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Summary

Isolation and culture of myofibers is the gold standard in vitro system to study the transition of satellite cells through quiescence, activation and differentiation. Importantly, the single myofiber culture system preserves the myofiber/stem cell association, which is an essential component of the muscle stem cell niche.

Abstract

Muscle regeneration in the adult is performed by resident stem cells called satellite cells. Satellite cells are defined by their position between the basal lamina and the sarcolemma of each myofiber. Current knowledge of their behavior heavily relies on the use of the single myofiber isolation protocol. In 1985, Bischoff described a protocol to isolate single live fibers from the Flexor Digitorum Brevis (FDB) of adult rats with the goal to create an in vitro system in which the physical association between the myofiber and its stem cells is preserved 1. In 1995, Rosenblattmodified the Bischoff protocol such that myofibers are singly picked and handled separately after collagenase digestion instead of being isolated by gravity sedimentation 2, 3. The Rosenblatt or Bischoff protocol has since been adapted to different muscles, age or conditions 3-6. The single myofiber isolation technique is an indispensable tool due its unique advantages. First, in the single myofiber protocol, satellite cells are maintained beneath the basal lamina. This is a unique feature of the protocol as other techniques such as Fluorescence Activated Cell Sorting require chemical and mechanical tissue dissociation 7. Although the myofiber culture system cannot substitute for in vivo studies, it does offer an excellent platform to address relevant biological properties of muscle stem cells. Single myofibers can be cultured in standard plating conditions or in floating conditions. Satellite cells on floating myofibers are subjected to virtually no other influence than the myofiber environment. Substrate stiffness and coating have been shown to influence satellite cells' ability to regenerate muscles 8, 9 so being able to control each of these factors independently allows discrimination between niche-dependent and -independent responses. Different concentrations of serum have also been shown to have an effect on the transition from quiescence to activation. To preserve the quiescence state of its associated satellite cells, fibers should be kept in low serum medium 1-3. This is particularly useful when studying genes involved in the quiescence state. In serum rich medium, satellite cells quickly activate, proliferate, migrate and differentiate, thus mimicking the in vivo regenerative process 1-3. The system can be used to perform a variety of assays such as the testing of chemical inhibitors; ectopic expression of genes by virus delivery; oligonucleotide based gene knock-down or live imaging. This video article describes the protocol currently used in our laboratory to isolate single myofibers from the Extensor Digitorum Longus (EDL) muscle of adult mice (6-8 weeks old).

Protocol

All experiments were handled according to the University of Ottawa regulations for animal care and handling.

See Table 1 for an overview of the protocol.

1. Before Starting the Isolation

Prepare the following solutions:
0.2% Collagenase type I in DMEM (Dulbecco's modified Eagle's medium; high glucose, L-glutamine with 110 mg/ml sodium pyruvate). For two EDL muscles prepare 2 ml of 0.2% Collagenease in DMEM. Filter the solution through 0.22 μm filter. 10 min before the isolation, prewarm at 37 °C in a water bath. Additional aliquots of undiluted collagenase can be frozen at -20 °C for later use.Note: use DMEM with sodium pyruvate throughout all of the procedure. Fibers do not survive in sodium pyruvate-free medium.

Washing media (use to perform all the washes). Supplement DMEM with 1% Penicillin/Streptomycin. Filter through 0.22 μm filter before use.

Matrigel coated dishes. To culture fibers for long period of time, we recommend using Matrigel as coating substrate. To prepare Matrigel coated dishes, thaw an aliquot of Matrigel at 4 °C overnight. The day after, dilute Matrigel 1:10 in DMEM. Keep Matrigel at 4 °C at all times and avoid abrupt temperature changes as this will create microscopic crystals within the Matrigel solution resulting in uneven coating. Place dishes to be coated on ice. Coat dishes with just enough volume to cover the surface. Let it sit for 1 min. Completely remove the leftover Matrigel. Let dishes dry at 37 °C for at least 3 hr prior to use or overnight.

Note: aliquots of diluted Matrigel can be re-used multiple times for coating purpose if stored at 4 °C.

Lastly, be sure to clean the microscope station and dissecting tools with 70% ethanol.

Four dishes for the isolation (1 for muscle dissociation, 3 for serial washes). All dishes must be coated with horse serum (HS) to prevent myofibers from attaching to plastic. To coat, pipette 3 ml of horse serum into each dish, swirl to allow even coating, remove the horse serum and let the dish dry for at least 30 min. Add 4 ml of DMEM to each dish. Keep dishes at 37 °C in a 5% CO2 incubator prior to use.

Note: Horse serum can be re-used multiple times, if kept sterile. Alternatively, a solution of 10% HS in DMEM can be used to coat dishes. Use HS coated dishes throughout the whole protocol and when culturing myofibers on floating conditions.

One dish will be used to culture myofibers after the isolation. Alternative dish sizes or formats can be used for the final culture of myofibers depending on downstream applications. However, we do not suggest dish sizes larger than 60*15mm. Myofibers can be kept in suspension for no longer than 96 hr before hyper contraction occurs. For longer culture times, we recommend using Matrigel coated dishes or plates.

For one fiber isolation (2 EDL), prepare two sterile Pasteur pipettes: one large bore pipette for muscle handling and one small bore pipette for myofiber manipulation. Use a diamond pen to cut each glass pipette to the desired length and heat polish to smooth pipette's edges. By using the flame, curve the tip of the small bore pipette. This will help handling single fibers. Flame to sterilize. Coat each pipette with HS before use.

2. Muscle Dissection and Digestion

For the purpose of these experiments, 8 week old SV129, Pax7 CreERCklr;Rosa26TdTomato (Pax7Cre-TdTomato) and Myf5-Cre;Rosa26YFP were used.

Spray hind limbs with 70% ethanol. Pin the animal (face up) to a support board to have a better grasp of the hind limb during the procedure.

With the help of scissors, cut through the entire length of the limb and expose the underlying muscle. Remove the skin as well as any hair or fur (Figure 1A).

With a fine scissor, cut through the thin fascia without damaging the underlying muscles. Visually localize the EDL. The EDL is found in the anterior compartment of the hind limb just underneath the Tibialis Anterior (TA) muscle.

With the help of two forceps, expose the distal tendons.

Cut the distal tendons (of both the TA and EDL) with sharp Cohann-Vannas spring scissors.

With the help of forceps hold both TA and EDL muscles by their tendons and delicately pull the muscles up towards the proximal end. At this point you should be able to clearly see the EDL muscle just underneath the TA muscle. Now, separate the EDL from the TA muscle by pulling the two tendons in opposite directions (Figure 1B). Avoid stretching the EDL muscle while performing this operation as this will damage the myofibers.

Expose the EDL tendon. To better visualize the proximal tendon it may help at this point to remove the TA muscle. It may also help to cut off some the connective tissue around the knee (Figure 1C).

Cut the proximal tendon and gently remove the EDL (Figure 1D).

By holding the muscle through its tendons, transfer it to 2 ml of previously prepared collagenase solution. Incubate at 37 °C in a water bath.Note: for successful fiber isolation, it is important to isolate the EDL from tendon to tendon so that the myofiber integrity is maintained. Steps 2.3 to 2.9 can be performed under a dissecting microscope. Alternatively, the use of a magnifying glass may also help to have a better view of the muscles.

Repeat steps 2.3 to 2.9 to isolate the second EDL. Transfer the second EDL in the same tube. To avoid uneven digestion, isolation of the second EDL should be completed no more than 5 min after the first.Note 1: incubation time may need to be adjusted depending on collagenase activity. Longer or shorter incubation might be required depending on the size, age and/or muscle condition (e.g. fibrotic muscles need longer digestion time).Note 2: If examining satellite cells behavior under quiescence conditions, agitation during muscle digestion time may activate satellite cells 10.

During the digestion time, regularly check the muscle to avoid over-digestion. Stop the digestion when muscles start to loosen up and myofibers are visible. To stop digestion, carefully transfer both muscles to a prewarmed Petri dish with 4 ml of DMEM (dissociation dish). Use the large bore size pipette to perform this operation.Note: avoid muscle overdigestion as this inevitably results in the isolation of hyper contracted myofibers.

3. Single Myofiber Dissociation and Culture

To release myofibers, use the large bore glass pipette to flush the muscle with warm medium until fibers naturally start being released. Do not triturate the muscle as this will inevitably result in damaging fibers. Perform this and the following steps under a dissecting microscope.

Continue releasing myofibers until the desired number is reached. If the dish is required at room temperature for more than 10 min allow a 5 min (minimum) incubation at 37 °C, 5% CO2 to re-equilibrate the medium.Note: if medium reaches temperatures below physiological (37 °C) for an extended time myofibers will die.

Using the small size bore pipette, transfer live single myofibers to a new prewarmed dish (first of three consecutive washes). Handle each myofiber individually instead of transferring bulk of myofibers all at once. If necessary, incubate at 37 °C, 5% CO2 for 10-15 min to re-equilibrate the medium.

Repeat step 3.3 for 2 more times or until all dead myofibers and debris are removed. We recommend at least three consecutive washes for proper clean-up.Note: dead myofibers will appear as short and hyper contracted under the microscope light.

Incubate single myofibers at 37 °C, 5% CO2 in the last wash dish (DMEM only) for at least one hr prior to switching to culture medium. This allows myofibers to adjust to the in vitro conditions in the absence of serum. We found that immediate culture of myofibers in serum rich medium increases fiber shrinking.

After one hr, transfer myofibers to a new prewarmed dish or to the appropriate culture format depending on the downstream application. Culture fibers in high serum medium to allow satellite cell activation. Alternatively, different concentrations of serum or chicken embryo extract can also be used. Change medium every other day.

4. Downstream Applications

Immunostaining. Live myofibers can be fixed and stained at any time point during the isolation. Immunofluorescence can be performed on both floating and substrate-attached myofibers. If staining floating myofibers, use a small bore glass pipette to transfer myofibers from one solution to another. Alternatively, it is possible to keep myofibers in the same well throughout all the procedure and add/remove solutions using a glass pipette. Avoid standard aspiration as this will result in the removal of the myofibers as well. Briefly, completely remove culture medium; fix myofibers in prewarmed 4% paraformaldehyde (PFA) for 5 min. Extensively wash in PBS several times. Incubate myofibers in 1% glycine in PBS or other standard quenching solutions to minimize PFA background staining. If necessary, permeabilize myofibers with 0.1% Triton X-100 in PBS for 10 min followed by a 5 min wash in PBS. Incubate fibers in blocking solution (10% horse serum, 0.1% Triton X-100, 1% NaN) for 1 hr at room temperature or preferably overnight at 4 °C. Alternative blocking solutions may be used, depending on the antibody of interest. Wash once in PBS for 5 min. Incubate with the appropriate primary antibody diluted in blocking solution for 1 hr at room temperature or overnight at 4 °C. Wash fibers 3 times at 5 min per wash in PBS to remove any unbound antibody. Incubate with the appropriate secondary antibody for 45 min to 1 hr at room temperature. Wash 3 times at 5 min per wash in PBS. Counterstain nuclei with 1 mg/ml DAPI. If staining floating fibers, transfer each fiber to a glass slide suitable for microscopy. Remove any excess of PBS or medium. Apply mounting medium and then add coverslip. Proceed to visualize myofibers under a fluorescence microscope. See Figure 4 for representative immunofluorescence on EDL myofibers. Alternative staining procedures using stronger fixatives are described in Verma, M. et al.11 and Wosniak, A.C. et al.12.

Oligonucleotide or plasmid transient transfection. Live myofibers can be transfected with plasmid or siRNA for specific gene/s of interest. When using siRNA, double transfection is recommended for efficient gene knockdown. We suggest performing the first transfection after 8 hr from the isolation. Six hr after the transfection, replace with fresh medium. For siRNA transfection, we suggest starting by using a final concentration of 50 nM. Gene expression knockdown can be analyzed by RNA extraction or preferably by immunostaining.

Viral infection. Infection of live myofibers is possible although the incidence of cell death is higher than with oligo transfection and the efficiency of infection may be variable depending on muscle conditions and age. For instance, intact adult muscle myofibers are particularly non responsive to viral infection due to the presence of the basal lamina which has been shown to provide a protective barrier against host infection 13, 14. Lentiviral vectors are preferred over retroviral vectors because they can infect quiescent (non mitotic) cells. For viral infection, it is advisable to culture fibers on a Matrigel coated dish or plate and let myofibers adjust to media conditions for the first 24 hr.

Live Imaging. Live imaging of myofibers is particularly time consuming and necessitates a microscope equipped with a 37 °C, 5% CO2 chamber. It is useful when assessing the behavior of single satellite cells. Work done using this technique has been instrumental for the discovery of satellite cell heterogeneity and to study their behavior on fibers (15 and 16).

Representative Results

Here we described the isolation of single myofibers from the EDL muscle of adult mice. Successful myofibers yield depend on several factors, such as collagenase activity or muscle conditions or age. Most importantly, the isolation of the muscle from tendon to tendon results in long, intact myofibers from EDL muscle. Figure 1 shows a step by step graphical representation of the "tendon to tendon" isolation. Once the muscle is fully digested, myofibers are released by applying gentle pressure to the muscle. Figure 2A shows a representative picture of a myofiber isolation experiment after the first wash. At this point the culture contains a mixture of bundles of single myofibers which appear as long and shining tubular structures, hyper contracted myofibers which are dark and short and debris from the digestion process. By the end of at least three consecutive washes, only single live myofibers should remain in the dish for culture or downstream analysis (Figure 2B). Figure 2C shows a long, live fiber as compared to a hyper contracted fiber (C'). At the time of the isolation, satellite cells appear as tiny protuberances on the myofiber surface (Figure 3A). If maintained in serum rich medium, satellite cells activate, proliferate, migrate and eventually fuse into myotubes (B). After 15 days in culture, all myotubes express the Myf5 reporter YFP (C) suggesting that muscle regeneration in the adult is performed by cells that at some point during their development had expressed the myogenic determinant factor Myf5. All satellite cells express the paired box transcription factor Pax7 17. The reporter mouse line Pax7Cre-TdTomato can be used to trace satellite cells via the expression of the TdTomato fluorescent signal (Figures 3D and E). Figure 4 shows a representative immunofluorescence of double Pax7+/Myod satellite cells. Classically double Pax7+/Myod+ satellite cells are considered proliferative committed muscle progenitors which will either complete the differentiation program by down regulating Pax7 while maintaining Myod expression or return to quiescence by down regulating Myod and maintaining Pax7 expression 18

Figure 1. EDL muscle isolation from mouse hindlimb. A . Hindlimb of an 8 week old adult mouse. Arrows indicates the distal (knee) tendon and the proximal (foot) tendon. B. Anatomical position of the Tibialis Anterior (TA) muscle and the Extensor Digitorum Longus (EDL) muscle. C. By holding the EDL through the proximal tendon, the muscle is pulled toward the knee to expose the distal tendon. D. The distal tendon is cut and the EDL is released.

Figure 2. Representative results of a single myofiber isolation experiment. A . Bright field picture of a myofiber isolation experiment at the first wash step. Red arrow indicates live myofibers, white arrow indicates hyper contracted myofibers and yellow arrow indicates cells, myofiber or ECM debris. B. After consecutive washes in DMEM, only live myofibers remain. C and C'. Image represents a long intact live myofiber (C) and a short hyper contracted myofiber (C'). Bar 10 μm. Pictures were taken with a Zeiss Axio Observer Z1 microscope equipped with AxioCam HR.

Figure 3. Representative results of a single myofiber culture experiment. A . Bright field picture of a single, live myofiber with its associated satellite cell (arrow) right after the isolation (Time 0). B. Single myofibers were plated on Matrigel and cultured in serum rich medium for 15 days. White arrow indicates differentiated myotubes as compared to single cells (yellow arrow) C. Single myofibers from a Myf5Cre;RosaYFP mouse were cultured as in B. Arrow indicates Myf5 derived myotubes. D and E. Single myofibers from Pax7Cre;TdTomato were isolated and fixed right after. Arrows indicate Pax7 positive quiescent satellite cell (E, red). Nuclei were counterstained with DAPI (D). Bar: 50 μm. Pictures were taken with a Zeiss Axio Observer Z1 microscope equipped with AxioCam HR.

Figure 4. Example of immunofluorescence staining of satellite cells on myofibers. Single myofibers were isolated and cultured for 72 hr in floating conditions. Satellite cells on myofibers were stained for the satellite cell specific marker Pax7 (B, red) and the myogenic regulatory factor Myod (C, green). Nuclei were counterstained with DAPI (A). Bars: 50 μm. Pictures were taken with a Zeiss Axio Observer Z1 microscope equipped with AxioCam HR.

Muscle Dissection (5 min each muscle)

Tendon to tendon isolation

Sharp tools

Minimal muscle damage

Muscle Digestion (30-45 min)

Temperature sensitive

Avoid overdigestion

Fiber isolation

Avoid over manipulation of fibers

Eliminate debris with several washes

Fiber Culture (Up to 3-4 weeks)

Format: any

Coating: horse serum, Matrigel

Medium: basal or high serum

Table 1. Overview of the myofiber isolation protocol. The myofiber isolation protocol consists of 4 major steps. For each step, the approximate time and major critical points are discussed. For detailed discussion of each step, refer to the protocol text.

Discussion

The isolation and culture of single myofibers from intact muscles provides an excellent in vitro model to study the process of muscle regeneration. A unique feature of this system is the preservation of satellite cells in their physiological environment beneath the basal lamina. Most importantly, the technique can be used to investigate muscle stem cell behavior in both quiescence and activated states. Over the past 20 years, the myofiber culture system has provided meaningful insights into the biology of the satellite cell population with respect to both intrinsic and extrinsic determinants. By culturing individual myofibers, satellite cell heterogeneity with respect to myofiber, muscle type or regenerative potential has been addressed 15. Elaborate studies using live imaging of single cultured fibers allowed for the gaining information on satellite cell migration pattern 16. The acquisition of quantitative data is also possible. Although time consuming, it provides significant information on the distribution and occurrence of specific events (stem cells asymmetric division, proliferation and differentiation ratio, etc.). Together with previously described applications, protein or RNA extraction from single fibers is also possible, although isolation of pure population of satellite cells by FACS or other means may provide a better platform to investigate protein or gene expression changes at a molecular level. In our experience, the most critical step for successful fiber isolation is the "tendon to tendon" isolation (steps 2.5 to 2.9 in the protocol text). This guarantees that after muscle digestion, fibers are released from the EDL with minimal or no damage thus increasing their performance in the following steps.

Disclosures

No competing interests.

Acknowledgments

We would like to thank Sarah Dick for providing critical reading and comments. M.A.R. holds the Canada Research Chair in Molecular Genetics and is an International Research Scholar of the Howard Hughes Medical Institute. This work was supported by grants to MAR from the National Institutes of Health, the Howard Hughes Medical Institute, the Canadian Institutes of Health Research, the Muscular Dystrophy Association and the Canada Research Chair Program.

Materials

Name

Company

Catalog Number

Comments

Collagenase

Sigma-Aldrich

C0130-1g

Prepare fresh all times for optimal results. Additional aliquots of undiluted collagenase can be stored at -20 °C.

Hi Nicolas,
Thank you for your interest in our protocol!
here is a quick ref ( doi: 10.1371/currents.RRN1²94) on how to perform single fiber isolation from human biopsies. Hope this helps,
good luck with your research,
Alessandra

Hi! You mention that the fibers can be kept in basal medium. However while we started with really nice fibers after overnight in serum free medium most of the fibers appeared hypecontracted and generally no good, while they same prep was ok in the serum supplemeted medium. Do you have any advice about how to culture fibers for a few days in serum free conditions? Thanks
Rita

Hi Rita, our fiber culture medium is usually enriched with high concentration of serum but as we said in our protocol you can play around with it. the lowest concentration of serum I worked with was 5% horse serum and the fibers were fine. In washing media ( ie: no serum) you can keep them for several hours. Probably overnight is too long. Hope this helps, let me know if you have other questions. Bests, Alessandra.

Hi,
1. I've never looked into that. could be interesting to look at, using the fiber system. If we keep fibers on matrigel coated slides long enough we do observe spontaneous contraction;
2. We have protocol for siRNA trasfection using lipofectamine that works pretty well on our hands;
Hope this helps,
Alessandra

Hi,
I am interested in knocking down a gene in isolated fibers and was wondering whether you could provide me with your protocol for siRNA transfection (or a reference if you published) since you are successfully doing so. Thanks

we have done siRNA transfection on fibers at different time points and in our hands it works very well. for a 48 hours transfection, a double transfection works better. For short term transfection ( ie 24hrs) no need to perform a double transfection. we normally check if the siRNA works on primary myoblasts first and then we do ti on fibers. For more info, you can check the following ref F. Le Grand et al, Cell Stem Cell, 2009.
Cheers,
Alessandra

I was wondering if you know if this method is also suitable for stuying glucose uptake into isolated muscle fibers, and if so, how much fibers (and therefore mice) you kneed in order to perform a reliable assay (normally I use a 12 or 24 well plate with C2C12s, but since these cells only show little insulin-stimulated glucose uptake I would like to switch to a different system).

I've never done glucose uptake experiments on isolated myofibers but I found this paper describing a method to measure glucose uptake from individual single fiber from rats. A Novel Method to Measure Glucose Uptake and Myosin Heavy Chain Isoform Expression of Single Fibers From Rat Skeletal Muscle. they use epitrochlearis muscle and they report isolating between 5 to 30 fibers per muscle. from 2 EDL muscle of mice I normally get ~ 150-200 fibers but I've never try to prepare the fibers for glucose uptake experiment.
Good luck, I'd be curios to know how the experiment turn out though.
Cheers,
Alessandra

thanks for your fast response. I think I'll just go and try some different methods (like incubating the whole muscle, or incubating all the isolated fibers of one leg) and see what works best. If I find anything that might be useful to add to your protocol I'll definitely let you know. The more people can learn something from this protocol, the better;)!

I'm facing the same problem with C2C12-cells and low insulin-stimulated glucose uptake. I wondered if you succeeded measuring glucose uptake from isolated fibers and if so, if you could provide your detailed protocol.

Yeah, these C2C12s are not the nicest model around... In the end I never got to trying the protocol with the isolated fibers, we decided to take a different approach to our problem. I guess I won't be able to help you any further, otherwise than advising you to steer clear of the C2C12s since they are so unreliable.
Nevertheless, lots of luck! I am sure that with Alexandra's protocol you will find a way to fix your problem:).
Vera

Thanks for the great video-article. I tried isolating mouse EDL fibers with a student of mine yesterday and have some specific questions.

1) We did not succeed in getting many fibers in our first go - can you provide a rough estimate of how many viable fibers you end up with and how long the isolation procedure normally takes you per muscle? How many isolation rounds do you normally do (using a healthy young (10 wks) wildtype C57BL/6 or similar)? Just so we know what to aim for:-)

2) The bulk of the muscles remained together and were hard to flush apart - I guess is too short collagenase treatment. Are there signs to watch for when judging if the muscle has had sufficient collagenase-exposure, like many fibers coming loose on the outside of the muscle?

3) Yesterday was just a pilot and we did not have matrigel yet. However, I noticed that the fibers were floating and clustering in the center of the wells. From your experience, are there any tricks to avoid entanglement and getting the fibers to settle onto the bottom of the plates/wells. Have you tried a mild centrifugation, for instance?

4) We would like to make a lysate and do some western blotting on the fibers to start with. Have you done any blotting, and could you in that case perhaps provide some advice on how to approach this. Do you just empty the wells and add your lysis buffer or does emptying the wells make the fibers hypercontract (as postulated in some protocols). How much do you lyse in/number of fibers and what are the detergents in your lysisbuffer?

Thanks a ton in advance.

Thom

PS: @ Vera above. I work with muscle glucose metabolism and multiple groups have performed and published measurement of fluorescent 2-deoxy glucose uptake into mouse single fibers (H. Westerblad in Sweden, for instance). Perhaps something to consider as an alternative to tracers:-)

Hi Thom,
I'm very happy you found this video useful. its a quite neat and informative technique indeed.
as for your questions, here are my suggestions:
1. normally from two EDL processed at the same time I get between 150 to 200 viable fibers at the end. there are more fibers at the beginning but then some will hyper contract and some will remain in bundles and some are maybe half hypercontrated and half alive so I discard them. this estimate is from a 6-8 wk old animal. Time wise, I'd say it takes me 1.5 to 2 hrs to complete the procedure. the physical dissociation of the 2 EDL shouldn't take more than 10 min, the collagenase incubation time varies between 30 to 45 min, the actual fiber dissociation time varies between 30 min to one hour, depending how many fibers I want at the end. I normally work with the muscle for 10-15 min then I put it back in the incubator for 5 min and then work again for other 10-15 and repeat this cycle till I have enough fibers. I'd say max time allowed for this step is one hour. I normally perform 3 washes, sometimes more than 3 if I have lot of debris or fibers. washes are normally very quick and again I incubate fibers in between every wash. before plating I let fibers rest for one hour in and then I plate. I find this extra step increases fiber viability.
2. I agree with you. My guess would be that the collagenase treatment wasn't long enough. I normally visually inspect for fibers coming out the muscle and stop when it reaches that point. too many fibers is not good sign. If i see one or two fibers coming out I then wait extra 2-3 min and then stop. old animals do require longer incubation time. it may also help agitate the tube a bit every so often to help the digestions process. some groups have reported that agitation activate satellite cells so it depends what you're looking for.
3. yes sometimes it does happen that fibers will cluster together in the middle of the dish. you can try increasing the number of washes to get rid of any piece of matrix still attached to the fibers. it also help transfer fibers from one dish to another one by one. it's pain sticking but that way they wont cluster all together as often. It's probably not that clear from the video but when I transfer fibers, I position my pipette in different places of the dish (middle, side, etc) so that fibers will be also be placed in different positions. when I walk from my station to the incubator I avoid moving the dish too much. I never swirl the dish containing the fibers. I've never tried centrifugation.
4. I've never perform WB on isolated single fibers. WB on whole muscle lysate is what we normally do.

Thanks a lot for the video, it has been very useful to get familiar with the fibers and have a protocol with images, which is always much more helpful.

I am interested in culturing the fibers to analyze the activated satellite cells by immunofluorescence.

I would like to know your opinion regarding the following issues.

• The most effective way to activate the satellite cells.
Is it easier to get them activated in suspension or attached to the culture dish?
Would you add growth factors to the culture medium? Or is it enough to culture the fibers in suspension with high percentage of serum (e.g. 20%)?
I usually find it difficult to get the fibers attached. When you culture them on matrigel-coated dishes, how long do they take to attach?

•The best way to perform immunofluorescence.
I tried to do it with the fibers attached on matrigel-coated surfaces, but they usually detach during the protocol.
I have also used polyester baskets, but the fibers get sticked to the net and I cannot recover them.
IF in suspension may be the best way, but when you transfer each fiber to the glass slide, how can you avoid getting too much liquid on it?

I would greatly appreciate if you could give me some advice or some additional guidelines to follow.

I'm glad you found our protocol useful.
Specifically about your questions here are my suggestions:
1.that's a very interesting point you're bringing up. I've never done a side by side comparison of satellite cells activation pattern in floating vs attached fibers. however, most satellite cells will be activated ( aka expressing ki67) at 48hrs regardless of whether you are culturing fibers in suspension or attached. similarly the first stem cell division usually occurs between 36 to 42 hours in floating or attached fibers but I'm not sure whether the kinetics are different. we do add CEE to our fiber media on top of adding 20% FBS to activate satellite cells. usually most fibers will attached to matrigel within few hours ( 5-6) from the plating or at most the day after. it happened to me that sometimes I would get few detaching or not properly attached fibers. this can be due to either matrigel being too old ( re-used too many times) or not properly handled. matrigel is very sensitive to temperature change. I normally use cold pipettes and work on ice at all time when coating with matrigel.
2. if you keep fibers on matrigel for like 15 days you need to be very careful when you do IF because fibers at that time will be more likely to detach. However satellite cells will all have migrated out the fibers. I' ve done IF at 2-3 days and I dont recall fibers be that sensitive to manipulation in those early time points. I normally angle my pipette to the side so that washing solution wont be directly pointed to the fibers. when I do IF with floating fibers you can either use a pap pen to contour your slide so that fibers wont be too dispersed and/or I normally aspirate excess PBS or washing solution before adding a coverslip trying obviously to avoid aspirating fibers.

hope this helps, let me know if you have additional questions,
Cheers,
Alessandra

I have tried the isolation twice now and I am mostly getting short hypercontracted fibers and hardly any long healthy ones. The isolation of the muscles seems perfect and then I digest the muscle with 0.2% collagenase for 35mins in the waterbath without shaking. Do you think you might have some useful hints for us?

you may want to adjust the incubation time ..if after the digestion the muscle gets apart easily but you only get hypercontracted fibers out, you may want to reduce your incubation time...if, on the other hand, the muscle is still intact and only few hypercontracted fibers are coming out, then you may want to increase your incubation time......also make sure your pipettes edges are smooth so that you don't damage the fibers.
Good luck,
Alessandra

Thank you very much for your work on the paper and the videos. The videos especially are extremely helpful. I am having a difficult time removing single fibers from the muscle bulk in the collagenase step. The last time I tried this I even increased the digestion time to 4 hours and I still am unable to remove a single fiber. Would an increase in concentration be more helpful? In general is it more useful to go by concentration (i.e. 1 mg/mL) or working unit (100U/mL)? Could you suggest a specific concentration either way? According to sigma aldrich the suggested stored concentration is 10 mg/mL so if one uses 0.2% overall concentration would the suggested concentration by 2 mg/mL? Thank you very much for your help! I really appreciate it!

Hi Anna,
Sorry I just read your message now. I never had any issue using mild digestion as recommended in the protocol, but if not, I'd say you could try increasing collagenase concentration. let me know how it goes.

Dear Alessandra ,
Like many others I am getting short hypercontracted fibers and/or fiber segments, I tried incubation times from 15 min up to 45 min with little success, I also tried muscle dissected with and without tendon part, Do you have any suggestion e,g by increasing collagenase concentration ?
- Rizwan

Hi Rizwan,
you could try increasing collagenase concentration. In my experience, however, hyper contracted fibers result from tissue over digestion. Alternatively you could try polishing the edges of your pipette to make sure there are no sharp edges that may damage your fibers. another possibility is that you are cutting the EDL too close to its tendons. I usually expose the tendons first and then cut. The first few fibers will be hypercontracated but then you should mainly get live fibers. when I release fibers I try to not aspirate the EDL and I gently flush media.
Hope this helps,
Alessandra

Thanks Alessandra, this indeed is very helpful. I increased collagenase concentration and got good number of healthy shiny fibers released, I keep a healthy margin of tendon intact so I'm pretty confident there, I realize I need to spend more time in flushing to get reasonable number of fibers,
Many thanks
- Rizwan